Articles in PresS. Am J Physiol Lung Cell Mol Physiol (January 30, 2015). doi:10.1152/ajplung.00286.2014 Manuscript for the American Journal of Physiology - Lung Cellular and Molecular Physiology
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Pericytes contribute to airway remodeling in a mouse model of chronic allergic
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asthma
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Jill R. Johnson1, 2, *, Erika Folestad1, Jessica E. Rowley2, Elisa M. Noll2, Simone A.
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Walker2, Clare M. Lloyd2, Sara M. Rankin2, Kristian Pietras1, 3, Ulf Eriksson1 and
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Jonas Fuxe1
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Vascular Biology, Karolinska Institutet, SE-171 77 Stockholm, Sweden
Department of Medical Biochemistry and Biophysics, Matrix Division, Division of
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Building, Imperial College London, London SW7 2AZ, United Kingdom
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Leukocyte Biology Section, National Heart and Lung Institute, Sir Alexander Fleming
Lund University, Department of Laboratory Medicine Lund, SE-223 81 Lund, Sweden
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*Corresponding author: Jill Johnson, PhD, Leukocyte Biology Section, National Heart
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and Lung Institute, Sir Alexander Fleming Building, Imperial College London, London
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SW7
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[email protected] 2AZ,
United
Kingdom.
Phone:
+44
(0)
791-448-5692.
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Copyright © 2015 by the American Physiological Society.
Email:
Johnson et al.
Pericytes in airway remodeling
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Abstract
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Myofibroblast accumulation, subepithelial fibrosis and vascular remodeling are
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complicating features of chronic asthma, but the mechanisms are not clear. Platelet-
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derived growth factors (PDGFs) regulate the fate and function of various mesenchymal
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cells and have been implicated as mediators of lung fibrosis. However, it is not known
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whether PDGF-BB signaling via PDGFR, which is critical for the recruitment of
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pericytes to blood vessels, plays a role in airway remodeling in chronic asthma.
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In the present study, we used a selective PDGFRβ inhibitor (CP-673,451) to
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investigate the role of PDGFR signaling in the development of airway remodeling and
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lung dysfunction in an established mouse model of house dust mite (HDM) induced
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chronic allergic asthma.
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Unexpectedly, we found that pharmacological inhibition of PDGFRβ signaling in
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the context of chronic aeroallergen exposure led to exacerbated lung dysfunction and
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airway smooth muscle thickening. Further studies revealed that the inflammatory
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response to aeroallergen challenge in mice was associated with decreased PDGF-BB
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expression and the loss of pericytes from the airway microvasculature. In parallel, cells
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positive for pericyte markers accumulated in the subepithelial region of chronically
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inflamed airways. This process was exacerbated in animals treated with CP-673,451.
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The results indicate that perturbed PDGF-BB/PDGFR signaling and pericyte
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accumulation in the airway wall may contribute to airway remodeling in chronic allergic
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asthma.
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Keywords: asthma, house dust mite, airway hyperresponsiveness, pericyte, remodeling
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Johnson et al.
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Pericytes in airway remodeling
Introduction
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Asthma is a heterogenic disease that currently affects 300 million people
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worldwide (34). Allergic asthma is defined as an allergen-induced, immune-driven
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chronic lung disease manifested by recurrent episodes of airway inflammation
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composed of infiltrating eosinophils, mast cells, macrophages, neutrophils and
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lymphocytes (1). Airway remodeling is thought to be facilitated by this chronic
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inflammatory process (5). The structural changes associated with airway remodeling
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comprise goblet cell hyperplasia, collagen deposition and increased airway smooth
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muscle (ASM) mass, all of which contribute to the clinical manifestation of lung
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dysfunction (1). Inflammatory cytokines and the pro-fibrogenic growth factor
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transforming growth factor-β (TGF-β) are believed to play significant roles in driving
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these structural changes. However, the signaling mechanisms and the cellular sources
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from which the increased mesenchymal cell population of the airway wall is derived
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have not been fully described. Some studies have demonstrated that bone marrow-
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derived fibrocytes contribute to airway wall remodeling (30, 31), while others have
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suggested a minimal role for these cells (24). Additionally, the differentiation of
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mesenchymal cells from airway epithelial cells via epithelial-to-mesenchymal transition
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has been shown to be a mechanism of remodeling in a mouse model of severe allergic
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airways disease (20).
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The platelet-derived growth factors (PDGFs) are mitogens for a number of
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mesenchymal cell types, including fibroblasts and smooth muscle cells (9). The
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receptors of the PDGFs, PDGF receptor alpha (PDGFRα) and PDGF receptor beta
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(PDGFRβ) are tyrosine kinases, and are thus amenable to pharmacological
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Johnson et al.
Pericytes in airway remodeling
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intervention. However, little is known regarding the expression of the PDGFs in asthma,
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as the limited studies available in the literature have documented few differences in
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PDGF or PDGF receptor expression in human asthmatics compared to healthy controls
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(3, 6, 15, 25). Specifically focusing on PDGF-BB and its cognate receptor PDGFRβ in
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the context of allergic airway disease, stimulation of ASM cells with PDGF-BB in vitro
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has been shown to act in concert with TGF-β to stimulate cell migration (18). Moreover,
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a recent study using an adenovirus vector to overexpress PDGF-BB in the airway
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epithelium in an OVA-driven mouse model of asthma was shown to induce ASM cell
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proliferation and enhance airway hyperresponsiveness (14). PDGF receptors are also
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expressed on vascular mural cells, a heterogeneous population of mesenchymal cells
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that line the outer surface of microvessels and are therefore abundant in the lung (2).
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Pericytes, the population of mural cells covering capillaries, express desmin and NG2
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but are negative for α-smooth muscle actin (α-SMA), while mural cells covering
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arterioles and venules express desmin and α-SMA and are termed vascular smooth
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muscle (VSM) cells (2). Mural cells are recruited to and retained on blood vessels
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through PDGF-BB/PDGFRβ interactions (reviewed in (2)). Impaired pericyte coverage
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of blood vessels is seen in PDGF-BB-deficient mice and in diseases like cancer, and is
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associated with vascular leakage and edema (2, 4, 32).
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In light of these findings, and since tyrosine kinase inhibitors such as masitinib
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are currently being investigated as asthma therapies (16), we elected to investigate the
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impact of PDGFRβ inhibition on airway and VSM cells/pericytes in a mouse model of
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chronic aeroallergen exposure driven by exposure to house dust mite (HDM) extract via
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the respiratory mucosa. HDM exposure is strongly associated with human asthma and
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is one of the most ubiquitous respiratory allergens worldwide. In mice, chronic
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respiratory HDM exposure leads to Th2-polarized airway inflammation, remodeling of
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the airway wall and bronchial hyperreactivity, and thus recapitulates many of the
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features of clinical asthma (21). Using this paradigm, we investigated the role of
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PDGFRβ signaling and the downstream effects of inhibiting this receptor during chronic
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HDM exposure on airway remodeling and lung dysfunction.
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Materials and methods
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Animal handling
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Female C57Bl/6 mice were bred in-house at the Karolinska Institutet animal facility at
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the Department of Mikrobiologi, Tumör- och Cellbiologi (MTC) or purchased from Harlan
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Laboratories (Wyton, UK) and housed at the central animal facility at Imperial College
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London. Transgenic mice used for pericyte lineage tracing studies (Tg(Cspg4-
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DsRed.T1)1Akik/J) were obtained from the Jackson Laboratories (Bar Harbor, ME); the
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phenotype of these mice was determined by direct fluorescent imaging of the DsRed
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fluorescent signal in ear biopsies. Animals were initiated into experiments at 8-12 weeks
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of age. Mice were housed under specific pathogen-free conditions following a 12-h light-
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dark cycle and were provided food and water ad libitum. All experiments described in
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this study were approved by the Research Ethics Committees at the Karolinska Institute
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and at Imperial College London and were performed in accordance with the UK Home
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Office and Imperial College London guidelines on animal welfare.
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Antigen and drug administration 5
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Mice were challenged with purified Dermatophagoides pteronyssinus extract (HDM)
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(Greer Laboratories, Lenoir, NC, USA) 5 days per week for 3 or 5 consecutive weeks.
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HDM was re-suspended in sterile phosphate buffered saline (PBS) (2.5 mg of
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protein/ml); 10 μl of HDM were administered intranasally to isoflurane-anesthetized
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mice (Sigma-Aldrich, Gillingham, UK) (21). Control mice were subjected to the same
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exposure protocol but received PBS (10 μl). In each group, a subset of animals received
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a selective PDGFRβ inhibitor (CP-673,451 (Pfizer Inc., New York, NY, USA)) by oral
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gavage (33 mg/kg in polyethyleneglycol 400 (PEG-400; Sigma-Aldrich) daily for a period
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of 5 consecutive weeks. Other animals received the drug vehicle (PEG-400). 1-(2-(5-(2-
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methoxy-ethoxy)-benzoimidazol-1-yl)-quinolin-8-yl)-piperdin-4-ylamine
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has 10-fold higher affinity for PDGFR versus PDGFR, and greater than 450-fold
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higher affinity for PDGFR versus c-kit, and was prepared according to the procedures
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described previously (27).
(CP-673,451),
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Lung function measurements
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After 5 weeks of allergen and drug administration, mice were subjected to lung function
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measurements (8). Mice were injected intraperitoneally with sodium pentobarbital (50
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mg/kg) (Sigma-Aldrich), followed by an intramuscular injection of ketamine (90 mg/kg)
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(Sigma-Aldrich) (29). Mice were tracheostomized using a 19-gauge blunt-ended needle.
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Measurements of dynamic airway hyperresponsiveness (AHR) and elastance were
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acquired using the flexiVent system (Scireq, Montréal, Canada). Mice were ventilated,
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and airway resistance and elastance were calculated as previously described (29). A 4-
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6 µm nebulizer was used, and the duration of nebulization was 10 seconds per dose. A
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50% duty cycle was used during nebulization. Fluctuations in AHR and elastance were
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determined by the responses of the total respiratory system to increasing
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concentrations (10-300 mg/ml) of methacholine (MCh) (Sigma-Aldrich) delivered into
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the inspiratory line of the flexiVent ventilator. The PaO waveform was monitored
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throughout flexiVent data acquisition and was found to be similar during measurements
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as when the initial calibration was performed before running each subject.
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Measurements were not taken when there were obvious signs of respiratory effort.
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Following flexiVent data acquisition, the thoracic cavity of each mouse was opened to
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confirm that cardiac arrest had not occurred.
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Collection of specimens
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Mice were humanely sacrificed and the lungs were dissected. In some experiments,
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bronchoalveolar lavage (BAL) was collected (0.45 ml of PBS). BAL cells were counted
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using a hemocytometer, centrifuged at 1200 rpm for 5 minutes, then mounted on glass
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slides using a Cytospin (Thermo Scientific, Hemel Hempstead, UK) and stained with
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hematoxylin and eosin for differential cell counts. BAL supernatants were stored at -
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20ºC, then submitted to ELISA to determine mouse PDGF-BB expression according to
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the manufacturer’s instructions (R&D Systems, Abingdon, UK). In other experiments,
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mice were perfused through the left ventricle with 1% paraformaldehyde, and the
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trachea, extrapulmonary bronchi and lung were dissected out. The tracheas,
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extrapulmonary
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paraformaldehyde for 30 min, then transferred to PBS. The lung was embedded in
bronchi
and
lungs
were
isolated
and
preserved
in
1%
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Johnson et al.
Pericytes in airway remodeling
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OCT, stored at -80°C and cut into 10 μm thick sections for staining. Fresh lung samples
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were snap-frozen for qPCR and immunoblotting experiments.
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Immunoblotting
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Frozen lung tissue specimens were homogenized in 400 μl of lysis buffer, which was
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composed of T-PER Tissue Protein Extraction Reagent (Rockford, IL) supplemented
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with protease inhibitors (Complete Mini tablets from Roche Diagnostics Scandinavia,
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Bromma, Sweden), and homogenized with a homogenizer (Percell, Stockholm,
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Sweden). Protein samples were separated by SDS-PAGE on 4-12% polyacrylamide
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gels and blotted onto nitrocellulose membranes. The membranes were incubated in
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blocking buffer (5% skim milk) in Tris-buffered saline containing 0.5% Tween for 1 hour
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at room temperature and probed with a polyclonal rabbit-antihuman PDGF-BB antibody
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(Aviva Systems Biology, San Diego, CA) diluted 1:1000 in blocking buffer. After
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washing, the membranes were incubated with a HRP-conjugated secondary anti-rabbit
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antibody (GE Healthcare, Stockholm, Sweden) diluted 1:5000 in blocking buffer, for 1
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hour at RT. The membranes were developed using ECL+ detection reagent
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(Amersham, GE Healthcare). To ascertain equal loading of protein, the membranes
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were stripped and re-probed with a rabbit-anti-mouse antibody against Akt (Cell
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Signaling/BioNordika Sweden, Stockholm, Sweden) diluted 1:1000 in blocking buffer.
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Immunofluorescent staining
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Lung sections from C57Bl6 and DsRed-NG2 mice were warmed to room temperature
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and non-specific binding was blocked by incubating in 5% normal goat serum (NGS),
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0.3% Triton-X 100 and 0.1% bovine serum albumin (BSA) (all purchased from Sigma-
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Aldrich) in PBS for 1 h at RT. Sections were stained using the appropriate primary (O/N)
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and secondary (1 h) antibodies (Table 1). After washing twice in PBS, sections were
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mounted using a glycerol-based mounting medium containing DAPI (Vector
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Laboratories, Peterborough, UK) to visualize DNA. For polyclonal antibodies, negative
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reagent controls were carried out.
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For
tracheobronchal
whole
mount
immunostaining,
the
trachea
and
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extrapulmonary bronchi were dissected and cleaned of connective tissue and mounted
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on KwikgardTM-coated (WPI, Sarasota, FL, USA) 6-well culture plates. Non-specific
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binding was blocked by incubating trachea sections in 5% NGS, 0.3% Triton-X 100 and
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0.2% BSA in PBS O/N. Left and right trachea sections were stained using the
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appropriate primary and secondary antibodies O/N at RT (Table 1). Sections were
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washed thrice in PBS and mounted using a glycerol-based mounting medium containing
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DAPI (Vector Laboratories). For all antibodies, negative reagent controls were carried
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out with no staining observed.
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Light microscopy
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Quantification of αSMA and NG2 positive cells in the trachea and extrapulmonary
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bronchi was performed using a Leica DM2500 fluorescence microscope (Leica
197
Microsystems, Milton Keynes, UK). Counts were normalized to the length of each
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tracheobronchal whole mount (including the extrapulmonary bronchi at the distal end of
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the preparation). For image acquisition from immunostained tracheobronchal whole
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mounts and lung sections, 1024 x 1024 pixel RGB-color images were obtained using a
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Zeiss LSM 510 inverted confocal microscope with argon, helium-neon and UV lasers
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(Carl Zeiss AG, Göttingen, Germany) using an EC Plan-Neofluar 40x/1.30 oil objective
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with the DIC phase contrast technique (10). Using the optimized pinhole size, 0.9 μm
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thick optical sections were sequentially collected with a step size of 1 μm (lung sections)
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or 1.5 μm (tracheas). Image analysis was performed using Zeiss AIM 3.2.2 software
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and Zeiss LSM Image software (Carl Zeiss AG). Three-dimensional visualizations
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(Videos 1-4) of confocal images were prepared using Volocity software (Perkin-Elmer,
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Waltham, MA). Morphometric analysis of ASM thickness was performed by a blinded
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observer on αSMA-stained lung sections and analyzed using ImageJ software (NIH,
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USA). Morphometric analysis of the number of NG2+ cells in the airway subepithelial
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region was conducted by a blinded observer on lung sections stained for NG2, SMA
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and CD31 (to prevent enumeration of pericytes associated with the microvasculature).
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Five representative images were taken of the large airways (bronchi and bronchioles)
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from each animal (n=5-10 per group from two independent experiments). Images were
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taken on a Zeiss LSM 510 inverted confocal microscope and processed using ImageJ.
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NG2+ cells in the airway subepithelial region were enumerated and counts were
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normalized to mm of basement membrane.
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Quantitative PCR (qPCR)
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Whole tissue RNA from lung was isolated with TRIzol reagent (Invitrogen/Life
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Technologies, Stockholm, Sweden) and QIAGEN RNeasy (Qiagen, Sollentuna,
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Sweden) according to the manufacturers’ instructions. Total RNA (1 μg) was reverse
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transcribed according to the manufacturer’s instructions (iScript cDNA synthesis kit, Bio-
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Rad). qPCR was performed using Platinum SYBR green SuperMix (Invitrogen) and
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25 ng cDNA per reaction. Primers used were: Pdgfb QT00266910, Pdgfrb QT00113148,
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L19 QT01779218. Ct values for the three genes analyzed were: 19-20 (PDGF-BB); 24-
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26 (PDGFRβ); 17-18 (L19). Expression levels were normalized to the expression of
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L19. Melt curves were assessed following the completion of RT-PCR to ensure that the
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fluorescent signal resulted from a single PCR product.
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Data analysis
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Data were analyzed with GraphPad Prism Software version 6 (GraphPad Software, San
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Diego, CA, USA). Statistical analysis was performed by Student’s t-test or one-way
234
analysis of variance (ANOVA) with a subsequent Tukey post-hoc test where
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appropriate. Differences were considered statistically significant when p